The glucocorticoid (GC) receptor (GR) suppresses inflammation by activating anti-inflammatory and repressing pro-inflammatory genes. GR-interacting protein-1 (GRIP1) is a GR corepressor in macrophages, however, whether GRIP1 mediates GR-activated transcription, and what dictates its coactivator versus corepressor properties is unknown. Here we report that GRIP1 loss in macrophages attenuates glucocorticoid induction of several anti-inflammatory targets, and that GC treatment of quiescent macrophages globally directs GRIP1 toward GR binding sites dominated by palindromic GC response elements (GRE), suggesting a non-redundant GRIP1 function as a GR coactivator. Interestingly, GRIP1 is phosphorylated at an N-terminal serine cluster by cyclin-dependent kinase-9 (CDK9), which is recruited into GC-induced GR:GRIP1:CDK9 hetero-complexes, producing distinct GRE-specific GRIP1 phospho-isoforms. Phosphorylation potentiates GRIP1 coactivator but, remarkably, not its corepressor properties. Consistently, phospho-GRIP1 and CDK9 are not detected at GR transrepression sites near pro-inflammatory genes. Thus, GR restricts actions of its own coregulator via CDK9-mediated phosphorylation to a subset of anti-inflammatory genes.
Inflammation is a host response to infection or injury triggered when innate immune cells such as macrophages identify pathogenic molecules via pattern recognition receptors (for example Toll-like receptors (TLR)) and initiate an inflammatory gene expression program executed primarily by the effector transcription factors NF-κB and AP11. Although normally protective, inflammation is potentially dangerous to the host and contributes to the pathogenesis of numerous human pathologies including rheumatoid arthritis, lupus, multiple sclerosis, and others2. Hence, several mechanisms have evolved that limit inflammatory responses at the local and systemic level. In particular, inflammatory mediators trigger the production of glucocorticoids (GC), steroid hormones with profound anti-inflammatory properties3. GCs signal through the GC receptor (GR), a ligand-dependent transcription factor of the nuclear receptor (NR) superfamily that, upon hormone binding, is recruited to genomic GC response elements (GRE) to regulate gene expression4. Several classes of GREs have been described: at palindromic GREs, GR binds DNA directly and typically activates target genes, including anti-inflammatory mediators such as Dusp1 and Gilz 5,6. Equally common are “tethering” GREs, where GR associates with other DNA-bound regulators, most prominently NF-κB or AP1, and represses their pro-inflammatory target genes (including Tnf and Il1b)7. Activation of anti-inflammatory and repression of pro-inflammatory genes both critically contribute to the therapeutic efficacy of GCs, which have been exploited in medicine for over half a century8,9,10,11.
To exert transcriptional effects, GR assembles multi-subunit protein-DNA complexes composed of numerous coregulators. In addition to linking sequence-specific transcription factors with basal machinery and chromatin, coregulators integrate diverse environmental signals and transcription programs to ultimately elicit an appropriate physiological response. Prominent NR cofactors are the members of NR coactivator (NCoA)1-3 p160 family, which provide binding platforms for secondary coregulators and chromatin modifiers, for example, histone acetyltransferases (CBP/p300) and methyltransferases (G9a, CARM1) (reviewed in refs. 12,13). NCoA1-3 were originally identified as interactors of agonist-bound NRs and found to serve as coactivators in overexpression studies14,15,16,17. Functional redundancy between p160s has been supported by ~60% similarity across their NR-interaction domain as well as their activation domains 1 and 2 that bind CBP/p300 and CARM1, respectively13,18,19. Yet, subsequent in vivo studies with mice revealed non-redundant, sometimes antagonistic functions for these proteins in immune, metabolic and reproductive physiology and pathology (reviewed in refs. 12,13,19). Given the ability of these coregulators to cooperate with numerous NRs and non-receptor transcription factors, however, the exact transcriptional pathways responsible for the observed unique phenotypes of p160 deficiencies in vivo in different cell types remain largely undefined.
In regards to GC signaling, NCoA2 (also known as GR-interacting protein (GRIP)1)15,16 has emerged as a unique family member that, unlike other p160s, associates with GR at “tethering” sites and facilitates GC repression of AP1- and NF-κB-driven targets20,21. Indeed, GRIP1 deletion in macrophages derepresses genes encoding inflammatory mediators in vitro and sensitizes mice to TLR4-induced systemic inflammation in vivo22. In contrast, whether GRIP1 contributes to GR-mediated gene activation in macrophages, or in pertinent physiological settings in a manner that cannot be compensated by other p160s has never been evaluated. Given that intracellular levels of individual p160 family members vary among different cell types, and that the abundance of GRIP1 in murine macrophages is low23, it is possible that GRIP1 recruitment to distinct GR transcription complexes is stochastic and transcriptional complexes effectively compete with each other for limiting amounts of GRIP1. Alternatively, there could be signals that direct GRIP1 to specific genomic GR binding sites (GBS) or gene classes. Finally, it remains unexplored how the stimulatory vs. inhibitory properties of this bifunctional coreguator are specified. In principle, the allosteric effects of interacting complex components may dictate GRIP1 function as a coactivator or a corepressor; it is also possible that additional regulatory inputs constrain GRIP1 activities to operating as one or the other.
Our group previously reported that, in response to GCs, GRIP1 is phosphorylated at four serines, S469, S487, S493, and S499, outside any characterized functional domain, in a GR:GRIP1 interaction-dependent manner22,24. Post-translational modifications (PTM) of proteins are known to affect their biochemical and functional characteristics including stability, subcellular localization and protein:protein interactions. In the case of transcriptional cofactors, such as the p160s, PTMs would be expected to potentiate or attenuate gene expression programs (reviewed in refs. 12,13,19),conceivably, in a cell context-specific manner. Nonetheless, the importance of GRIP1 phosphorylation in inflammation and biology of macrophages, a cell type in which GR actions bear therapeutic value, has not been reported.
Here we investigate the function of GRIP1 as a GR coactivator in mouse and human macrophages by assessing GR-driven gene expression after GRIP1 deletion and global GR and GRIP1 genome-wide distribution. We further present evidence that GR, by recruiting the GRIP1 kinase, sets up a versatile and precise mechanism to ensure GRIP1 modification in a GBS-specific manner. Finally, we dissect the functional implications of GC-induced GRIP1 phosphorylation with respect to its coactivator versus corepressor properties in GR-regulated gene expression in macrophages.
GRIP1 mediates GC induction of anti-inflammatory genes
The ability of GR to induce genes encoding anti-inflammatory mediators in macrophages critically contributes to the efficacy of GC therapies8,9,10,11. Indeed, in human THP1 differentiated macrophage-like cells (THP1 MΦ) and in mouse primary bone marrow-derived (BM)MΦ, a 2-h treatment with the synthetic GC dexamethasone induced expression of the canonical GR target Fkbp5 as well as genes with known anti-inflammatory function: SGK1, PER1, DUSP1, KLF9, A20, GILZ, IL10 and Sgk1, Per1, Dusp1, Klf9, Ccl17 and Gilz in human and mouse, respectively7,25,26,27,28,29,30 (Supplementary Fig. 1a). To test whether the p160 coregulator GRIP1 is necessary for this induction, THP1 MΦ stably depleted of GRIP1 via lentiviral-delivered small-hairpin (sh)RNA KD (shGRIP1; Supplementary Fig. 1b, left) or BMMΦ from LysM-CreGRIP1 fl/fl mice (GRIP1 KO31) and their respective scrambled-transduced (shSCR) or GRIP1fl/fl (WT) controls (Fig. 1a, b, left; see Supplementary Fig. 1b for the quantification of GRIP1 protein and RNA) were treated with dexamethasone for 2 h and gene expression compared. Figure 1a, b (right) show that GRIP1 depletion attenuated GC induction of all GR targets examined except for SGK1 (and anti-inflammatory gene MT2A 32, Supplementary Fig. 1c) in THP1 MΦ and Sgk1 in BMMΦ, whose regulation by dexamethasone appeared GRIP1-independent. Importantly, differences in GC induction of genes were not due to altered basal expression (Supplementary Fig. 1d). Together, these results suggested that endogenous GRIP1 performs non-redundant functions in GR-activated gene expression in macrophages.
Because no genome-wide analysis of GR and GRIP1 co-distribution in macrophages after acute GC exposure has been reported, we performed GR and GRIP1 ChIP-seq in macrophages treated with Dex for 45–60 min and compared their localization. Correlation between reads found in GR and GRIP1 peaks in individual replicates indicated considerable reproducibility of ChIP-seq experiments (Supplementary Figs. 2a, 3b and 4b). Consistent with ligand activation, very few GR binding events were detected in untreated cells (5 and 77 in THP1 MΦ and 103 in BMMΦ), whereas dexamethasone treatment triggered rapid GR mobilization with several thousand GBS detectable (Fig. 1c, d, Supplementary Figs. 2a and e, 3a and 4a). Even though GRIP1 does not bind GCs, dexamethasone treatment resulted in a dramatic increase in GRIP1 binding sites (~tenfold for THP1 MΦ and ~threefold for BMMΦ; Fig. 1c, d, top; Supplementary Figs. 3a, b, 4a, b). Strikingly, there was minimal overlap between the GRIP1 peaks ± dexamethasone (40 peaks in THP1 MΦ and 178 peaks in BMMΦ, Supplementary Figs. 3b, 4b). Moreover, under liganded conditions, 2286 (91%) and 903 (60%) of GRIP1 peaks in THP1 MΦ and BMMΦ, respectively, overlapped with GR peaks (Fig. 1c, d, top). These overlapping peaks in THP1 MΦ exhibited higher pileup values (Supplementary Fig. 3d), suggesting that these sites either have a higher affinity for GR or are in a more permissive chromatin environment.
Ab initio motif discovery/overrepresentation analyses with MEME-ChIP at GRIP1 sites overlapping GBS or of the GBS themselves in dexamethasone -treated macrophages showed an enrichment of NR3C sites, which includes GREs as principal binding motifs, within the peak (Fig. 1c, d, middle; Supplementary Fig. 2b, f) and near peak summits (Supplementary Figs. 2c, g and 3g). ETS, AP1, and CEBP motifs were also enriched within GBS with the ETS motif enriched near the summit in BMMΦ (Supplementary Fig. 2g). Of note, GBS motif analysis in THP1 MΦ identified a putative composite site containing a GRE half-site and IRF-like binding motif (Supplementary Fig. 2b), suggesting potential interactions between these classes of transcription factors. Further supporting a model whereby ligand dedicates GRIP1 to GR signaling, GRIP1 binding distribution mirrored that of GR—primarily distal intergenic (42–46%) and intronic (32–34%) (Fig. 1c, d, Supplementary Fig. 2a, e)—similar to GR binding distribution in other cell types33. Interestingly, pathway analysis of genes associated with GR–GRIP1 overlapping peaks revealed immune-related signatures in both human and mouse cells, in addition to cell adhesion pathways seen in THP1 MΦ and hypoxia and circadian clock signatures in BMMΦ (Supplementary Figs. 3h, 4f). Consistently, pathway analysis of GR peaks further supported extensive involvement of GR in regulating inflammation and innate immunity (Supplementary Fig. 2d, h).
In sharp contrast, there was a minimal overlap of GRIP1 peaks in untreated MΦ with those of liganded GR: 32 (13.4%) in THP1 MΦ and 13 (0.02%) in BMMΦ (Supplementary Figs. 3b, 4b). Notably, motif enrichment analysis for GRIP1 binding peaks in untreated MΦ revealed the overabundance of low-complexity sequences (centromeric, tri- and tetra-nucleotide repeats; Supplementary Figs. 3f, 4d) that likely represent non-specific or low affinity binding or artifacts of peak calling34. Further, we analyzed GRIP1-unique peaks in dexamethasone-treated THP1 MΦ (203 peaks in Fig. 1c and Supplementary Fig. 3c) and BMMΦ (611 peaks in Fig. 1d and Supplementary Fig. 4c). In both cell types, these peaks were enriched for low-complexity sequences with similarity to Tcf7, Tbp, and ETS binding sites (Supplementary Figs. 3h, 4e). GRIP1-unique peaks were also smaller (Supplementary Fig. 3d), suggesting either weaker DNA binding affinity for the factor recruiting GRIP1 or non-permissive chromatin. This result, combined with the lack of sizable overlap of these peaks between GRIP1 replicas (Supplementary Figs. 3c, 4c, bottom), is consistent with GRIP1 binding being largely signal (in our case, liganded GR)-driven in both species.
Given our results demonstrating the function of GRIP1 in GR target gene activation, we evaluated ChIP-seq read distributions at GR targets analyzed in Fig. 1a, b. Dexamethasone -induced GR and GRIP1 peaks colocalized at all GBS, except for the GBS at −1 kb of SGK1 or Sgk1 (Fig. 1c, d, bottom), whose induction was GRIP1-independent. GR and GRIP1 ChIP-seq results from both cell types were validated by ChIP-qPCR (Supplementary Fig. 1e). Together, these results implicate GRIP1 as a key GR coactivator, whose loss is responsible for the impaired GC induction of genes in GRIP1-depleted macrophages (Fig. 1a, b).
Although the THP1 cell line is commonly used to study MΦ functions35, we corroborated our findings in primary human macrophages differentiated in vitro from CD14+ monocytes. Figure 1e shows that a 2-h dexamethasone treatment of hMΦ induces FKBP5, PER1, DUSP1, and KLF9, and negatively regulates SGK1. Furthermore, GR and GRIP1 colocalized at the FKBP5, PER1, DUSP1, and KLF9 GBS, whereas only GR occupied the SGK1 GBS (Fig. 1f), recapitulating the THP1 results.
CDK9 phosphorylates GRIP1 in a GC-dependent manner
We previously showed that GRIP1 is phosphorylated at a cluster of serines—S469, S487, S493, and S499—in a dexamethasone- and GR:GRIP1 interaction-dependent manner24. Because that work was performed primarily in a U2OS osteosarcoma cell line overexpressing GR36, we questioned whether phosphorylation was conserved in macrophages, a key innate immune cell type in which anti-inflammatory actions of GCs are physiologically relevant. Immunoblotting of hMΦ, THP1 MΦ and BMMΦ using phosphosite-specific antibodies to pS469, pS487, pS493, and pS49924 revealed dexamethasone-induced phosphorylation of each serine without a change in total GRIP1 or GR levels (Fig. 2a; quantified in Supplementary Fig. 5a). Interestingly, these serines were phosphorylated with varied kinetics depending on specific site and species.
To identify the kinases potentially responsible for GRIP1 phosphorylation in macrophages, we tested a panel of kinase inhibitors and found that flavopiridol (FVP), a CDK9 inhibitor, abrogated dexamethasone-dependent GRIP1 phosphorylation in both THP1 MΦ and BMMΦ (Fig. 2b, quantified in Supplementary Fig. 5b). Because chemical inhibition may suffer from limited selectivity, we knocked down CDK9 in immortalized BMMΦ (IBMMΦ) via lentiviral transduction of CRISPR–Cas9 gRNA against CDK9 (Supplementary Fig. 5c). Notably, CDK9 is required for transcriptional elongation by RNA polymerase II (Pol II)37,38, and its complete ablation would adversely affect cell viability. Strikingly, we found that CDK9 KD efficiency of ~60% correlated well with the relative loss of dexamethasone-induced GRIP1 phosphorylation (Fig. 2c). To determine whether CDK9 can directly utilize GRIP1 as a substrate, we performed in vitro kinase assays using baculovirus-expressed cyclin T1/CDK9 complex and a recombinant GST–GRIP1322–631 fragment containing the four target serines or mutant alanines (4A). CDK9 phosphorylated WT GRIP1322–631, but not a 4A mutant (Fig. 2d), establishing that CDK9 can directly phosphorylate the 4S cluster in vitro. Further supporting a direct mechanism, GR co-IPs from BMMΦ and THP1 MΦ revealed dexamethasone-induced GRIP1:GR:CDK9 ternary complex formation (Fig. 2e).
To interrogate whether CDK9’s role as a GRIP1 kinase could be uncoupled from its role in transcriptional activation, we treated cells with triptolide, a global inhibitor of Pol II-mediated transcription. As expected, triptolide induced Pol II degradation39 and blocked activation of GR target genes in both THP1 MΦ and BMMΦ (Supplementary Fig. 5d). Nonetheless, dexamethasone-induced FVP-sensitive phosphorylation persisted (Supplementary Fig. 5d) indicating that GRIP1 phosphorylation by CDK9 can occur independent of transcriptional activation. Given this result and that GRIP1 phosphorylation requires a GR:GRIP1 interaction24, we propose that GR recruits CDK9 to modify GRIP1. Additional evidence in support of this model is presented below.
Phosphorylation augments GRIP1 function as a GR coactivator
To assess the functional consequences of GRIP1 phosphorylation, we disrupted either the function of CDK9 or the GRIP1 phosphosites and evaluated GR target gene expression. CDK9 inhibition by FVP attenuated dexamethasone induction of a subset of genes in both THP1 MΦ (PER1, DUSP1, KLF9, GILZ) and BMMΦ (Fkbp5, Dusp1, Klf9, Ccl17), while leaving the induction of SGK1/Sgk1 unaffected (Fig. 3a), consistent with GRIP1 not participating in the activation of Sgk1 and ruling out a uniform effect of FVP on GR-mediated gene activation. Furthermore, the same genes affected by FVP in BMMΦ were sensitive to CDK9 depletion in IBMMΦ (Fig. 3b), corroborating a critical role of GRIP1 phosphorylation in GC induction of these genes in murine macrophages.
We next utilized our GRIP1-KD THP1 cells, which stably produce shRNA specific for hGRIP1 (Fig. 1a), to stably overexpress full-length murine WT or 4A GRIP1 via lentiviral delivery (Fig. 3c, left; Supplementary Fig. 6a). The inability of the mGRIP1 4A mutant to be phosphorylated in response to dexamethasone was confirmed by immunoblotting (Fig. 3c), with S487 phosphorylation being the best control as our anti-mouse pS487 antibody is species-specific and only recognizes exogenous mGRIP1 phosphorylation. Importantly, the loss of the 4S cluster in these mGRIP1 4A THP1-mutant MΦ resulted in attenuated induction of a subset of canonical and anti-inflammatory GR targets (FKBP5, PER1, DUSP1, GILZ) by dexamethasone, while MT2A was unaffected (Fig. 3d), consistent with its insensitivity to GRIP1 depletion (Supplementary Fig. 1c). As expected, the apparent effect of the 4A substitution was milder than that of kinase inhibition because overexpression of 4A GRIP1 should at least partially override its mutant phenotype.
Taken together, three different approaches in human and mouse macrophages point to an important regulatory function of GRIP1 phosphorylation in the GR-mediated activation of a specific panel of canonical and anti-inflammatory genes.
GRIP1 phospho-isoforms occupy distinct GR-bound sites
Our phosphosites of interest are within 30 aa of each other and may together form a novel GC-induced protein:protein interaction interface. Alternatively, distinct pGRIP1 isoforms with individual phospho-serines present in different combinations may occupy specific GBS. We explored these possibilities by ChIP-qPCR in THP1 MΦ and BMMΦ using phosphosite-specific antibodies and antibodies against CDK9. Consistent with the absence of GRIP1 at the SGK1/Sgk1 GBS (Fig. 1c), neither pGRIP1 nor CDK9 was detected at this site in THP1 MΦ or BMMΦ (Fig. 4a, b) despite the expected dexamethasone-induced recruitment of CDK9 to the SGK1/Sgk1 TSS (as well as those of FKBP5/Fkbp5 and PER1/Per1) as part of transcription elongation machinery (Supplementary Fig. 6b). In contrast, at GBS with dexamethasone-dependent enrichment of GRIP1 (Fig. 1c—THP1: FKBP5 +91k, PER1 +0.6k, DUSP1 -5k; BMMΦ: Fkbp5 +97k, Dusp1 -26k, Klf9 -84k, Ccl17 +1.6k), GRIP1 was variably phosphorylated and CDK9 was co-recruited (Fig. 4a, b). Indeed, at the PER1 GBS in THP1 MΦ and the Klf9 GBS in BMMΦ, GRIP1 was phosphorylated at every serine except S487; similarly, at the Ccl17 GBS in BMMΦ, GRIP1 lacked S493 phosphorylation; whereas all four serines were modified at other GRIP1-occupied GBS tested. Thus, GRIP1 phosphorylation is not uniform, but may be acting as a code dictating distinct GRIP1 functions at specific genes.
To test how widespread GRIP1 phosphorylation is at the genomic level, we performed pS469-GRIP1 ChIP-seq in THP1 MΦ. Similar to total GRIP1 peaks in untreated cells, pS469 peaks in untreated cells showed minimal overlap between replicas, lower average read counts per peak than in dexamethasone-treated cells and an enrichment of low-complexity sequences in motif overrepresentation analysis (Supplementary Fig. 7a–b). Conversely, using ChIP-seq data from untreated cells as background (Supplementary Fig. 7c–h), we observed that roughly 3/4 of dexamethasone-induced pS469 peaks (1213 of 1676) overlapped with GR peaks and that GRIP1 was phosphorylated at this residue at 44% (996 of 2286 peaks) of its total binding sites (Fig. 4c, Supplementary Fig. 4c). Consistent with dexamethasone-induced total GRIP1 cistrome, among GRIP1:pS469-GRIP1-overlapping peaks, NR3C and ETS motifs were highly overrepresented and NR3C was centrally enriched (Fig. 4c, Supplementary Fig. 7e, f). Similar to GRIP1 cistrome, genes associated with GRIP1:pS469-GRIP1-overlapping peaks belonged to immune-related pathways (Fig. 4c, right panel). We next evaluated read distributions and confirmed pS469-GRIP1 peaks at FKBP5 +91k, PER1 +0.6k, DUSP1 −5k, and KLF9 +17k (Supplementary Fig. 7g). Strikingly, we identified additional GBS associated with anti-inflammatory targets at which GRIP1 was S469-phosphorylated (NFKBIA +13.7k), unphosphorylated (IL1R2 -2k), or exhibited differential phosphorylation at GBS clusters (at least two sites within 5 Kb from each other) related to the same gene (A20 −49k vs. −56k) (Fig. 4d, e). In fact, clusters of GR:GRIP1 binding sites often displayed differential S469 phosphorylation: see FAM53B, RDX, and ST14 (Supplementary Fig. 7h).
Given that CDK9 co-occupied GBS with pGRIP1, we speculated that activated GR recruits CDK9 to modify GRIP1 and that CDK9 recruitment in response to dexamethasone persists even in the absence of GRIP1. Indeed, in GRIP1-depleted (shGRIP1) THP1 MΦ or GRIP1 KO BMMΦ the dexamethasone-induced enrichment of GR and CDK9 was unchanged despite abrogated GRIP1 occupancy (Supplementary Fig. 8a–c).
Phosphorylation affects GRIP1 occupancy and function at GBS
In principle, phosphorylation may affect multiple GRIP1 functions including its stability, subcellular localization, recruitment to genomic binding sites and/or, ultimately, interactions with additional components of GR complexes or basal transcriptional machinery. Given that GRIP1 levels are unchanged by dexamethasone and FVP that alter GRIP1 phosphorylation status (Fig. 2) and that GRIP1 is a constitutively nuclear protein40,41,42,43, we tested whether GRIP1 phosphorylation is important for its localization to GBS. Comparing dexamethasone-treated MΦ ±FVP, we found that FVP did not affect GR recruitment but, as expected, dramatically reduced occupancy of pS469-GRIP1 in both THP1 MΦ and BMMΦ (Fig. 5a, b, top and middle). Interestingly, loss of phosphorylation correlated with a reduction of GRIP1 occupancy at the PER1 GBS in THP1 MΦ (Fig. 5a, bottom), suggesting that phosphorylation contributed to GRIP1 targeting or retention at this GBS. Conversely, GRIP1 occupancy at the FKBP5 or DUSP1 GBS in THP1 cells or the Fkbp5, Dusp1, Klf9, or Ccl17 GBS in BMMΦ was unaffected by FVP. Consistent with inhibitor data, dexamethasone-induced enrichment of WT and 4A mGRIP1 as well as CDK9 and GR, were indistinguishable between THP1-mutant MΦ lines (Fig. 5c). Given that loss of phosphorylation impaired the ability of GRIP1 to serve as a GR coactivator for these genes (Fig. 3), we envision a scenario in which phosphorylation of the serines generates novel surfaces for protein:protein interactions and facilitates events downstream of GRIP1 loading (for example, recruitment of secondary cofactors or communication with basal machinery).
GRIP1 corepressor function is phosphorylation independent
GRIP1 has emerged as an important GR corepressor at “tethering” complexes, in which GR is recruited to chromatin through protein:protein interactions with DNA-bound AP1 or NF-κB and represses their target genes (such as Tnf, Il1a, and Il1b)20,21,22. Given that repression of hundreds of pro-inflammatory genes by the liganded GR is a critical component of the therapeutic actions of GCs, we first confirmed the role of GRIP1 in glucocorticoid repression of lipopolysaccharide (LPS, a TLR4 agonist)-activated genes in THP1 MΦ or GRIP1 KO BMMΦ from the LysM-CreGRIP1 fl/fl mice, in which the contribution of GRIP1 to GR repression has not been evaluated. Consistent with our published results20,22, dexamethasone repression of LPS-induced IL1A/Il1a, IL1B/Il1b, and TNF/Tnf was attenuated in GRIP1-deficient macrophages of both species relative to their GRIP1-sufficient counterparts (Fig. 6a). Importantly, GRIP1 depletion did not affect the ability of LPS to induce these genes (Supplementary Fig. 9a), demonstrating that the difference in “fold repression” arises from attenuated function of GR.
To corroborate the anti-inflammatory function of GRIP1 in the LysM-CreGRIP1 fl/fl mice in vivo, we challenged the GRIP1 KO and matching WT mice with LPS (5 mg kg−1 intraperitoneally) and assessed the hallmarks of septic shock syndrome. Consistent with our published studies23, GRIP1-deficient animals displayed significantly higher mortality (*P < 0.05; Kaplan–Meier analysis and the log-rank test) and lost a greater amount of body weight than WT as early as 24 h post injection (Supplementary Fig. 9b). To evaluate gene expression changes in macrophages at the site of 12-h LPS exposure, we performed peritoneal gavages and sorted peritoneal macrophages (CD45+CD11b+; CD11c−CD3−B220−Gr1−; see Supplementary Fig. 9c for gating strategy). In line with in vitro results, relative expression of GR-sensitive pro-inflammatory cytokines Tnf, Il1a, and Il1b was greatly elevated, whereas that of GC-stimulated anti-inflammatory Ccl17 and, to a lesser extent, Klf9 was reduced in the GRIP1 KO macrophages compared to WT (Supplementary Fig. 9c). Interestingly, the anti-inflammatory gene Dusp1 known to be strongly induced by inflammatory signaling and additively by GCs7, was expressed at higher levels in the KO macrophages, consistent with their exaggerated inflammatory response. Importantly, the apparent attenuation of GC regulation in GRIP1 KO in vivo occurred despite significantly (P < 0.05; unpaired, two-tailed Student’s t-test) elevated levels of circulating endogenous GC corticosterone at 12 h post injection, corroborating the inability of these animals to control systemic inflammation (Supplementary Fig. 9b).
To test whether the 4S phosphorylation cluster was important for GRIP1 corepressor function, we compared GC repression of LPS-induced IL1A, IL1B, and TNF in THP1-mutant MΦ expressing WT or 4A mGRIP1 and found it to be indistinguishable (Fig. 6b). Given the apparent lack of a role for target serines in GRIP1 corepression, we assessed whether they were still phosphorylated under LPS+Dex repressing conditions. Unexpectedly, LPS greatly attenuated dexamethasone-induced GRIP1 phosphorylation at each serine in THP1 MΦ and BMMΦ (Fig. 6c; quantified in Supplementary Fig. 9d), raising the possibility that LPS treatment globally attenuated GRIP1 phospho-isoform occupancy and GR-mediated induction of genes that are pGRIP1-dependent. We investigated this scenario by comparing the dexamethasone-induced occupancy of GR, GRIP1, CDK9, and pGRIP1 at GR activation or repression binding sites ±LPS exposure. As expected from the “tethering” nature of GR repression complexes at κB sites, GR and GRIP1 were recruited to Il1a and Il1b in BMMΦ in the presence of dexamethasone+LPS only and not dexamethasone alone (Fig. 6e). Similarly, in THP1 MΦ (Fig. 6d), GR and GRIP1 recruitment to IL1A and IL1B κB sites was most apparent upon Dex+LPS co-treatment, despite a modest enrichment of GR and GRIP1 at the IL1B κB site with Dex alone, likely due to residual p65 and AP1 presence after phorbol myristate acetate-induced differentiation44,45. Interestingly, however, neither GRIP1 phospho-isoforms nor CDK9 were detected at κB sites of IL1A/Il1a or IL1B/Il1b (Fig. 6d, e), consistent with pGRIP1 not participating in GR repression complexes. In contrast, at GR-activated genes FKBP/Fkbp5, KLF9/Klf9, PER1, and Ccl17 the Dex-induced occupancy of GR, GRIP1, CDK9 and all GRIP1 phospho-isoforms was fully resistant to LPS (Fig. 6d, e and Supplementary Fig. 9e), suggesting that pGRIP1 can persist at many GR-induced genes despite the general reduction of GRIP1 phosphorylation (Fig. 6c). Accordingly, dexamentasone-dependent, FVP-sensitive activation of these genes was similarly unaffected by LPS (Supplementary Fig. 9f, g). Together, these data indicate GRIP1 phosphorylation in macrophages specifically facilitates coactivator properties, but is dispensable for GRIP1 corepressor functions (Fig. 7).
Transcriptional cofactors coordinate and stabilize large multi-protein complexes, integrate diverse upstream signals and, ultimately, transduce information to basal transcriptional machinery and chromatin. The p160s have emerged as critical cofactors of NRs, which represent an important class of therapeutic targets. Despite a growing appreciation of the importance of p160s from gene ablation studies, specific NR:p160 relationships in relevant contexts that underlie their KO phenotypes are missing. Here we show a non-redundant role of the p160 family member GRIP1 in the GR activation of a panel of canonical and anti-inflammatory genes in mouse and human macrophages. Indeed, other cofactors, including the other two well-expressed p160s, failed to compensate for GRIP1 loss, even under conditions of stable GRIP1 deletion.
Genome-wide analyses of GRIP1 distribution yielded two unexpected observations. First, our genomic analysis in macrophages of both species argues that under liganded conditions, GRIP1 is a dedicated GR cofactor. This commitment is supported by the predominance of GREs and other sequence motifs known to be targeted by GR in overlapping peaks and the dramatic dexamethasone-induced expansion of GRIP1 cistromes, which substantially overlap GR cistromes; this was in striking agreement with recent data on single-molecule imaging of GR:GRIP1 association with chromatin46. The second surprising finding was an overrepresentation of immune-related pathways associated with GR:GRIP1 binding sites in GC-treated macrophages. This result did not reflect GR:GRIP1 co-localization at tethering “transrepression” sites as our macrophages were not exposed to inflammatory triggers that promote AP1 or NF-κB mobilization, which is a prerequisite for the formation of GR tethering complexes. Indeed, no p65 motifs were enriched in any of our GRIP1 cistromes; instead, sites of GR:GRIP1 co-occupancy after dexamethasone exposure were dominated by palindromic GREs typically associated with direct GR-inducible targets. It is therefore likely that the immune signature of the overlapping cistromes comprises anti-inflammatory genes activated by GR, including Dusp1, Klf9, Il10, A20, or Ccl17. Combined, these data suggest that increased sensitivity to sepsis observed in our macrophage-specific GRIP1 KO and that of previously described GR KO mice22,47 in part stems from suboptimal GC activation of anti-inflammatory genes, in accord with several earlier reports5,47,48.
Given that GRIP1 has been implicated in multiple physiological processes, including reproduction, metabolism, and circadian clock31,49,50,51, it would be informative to assess the genomic relationships of GRIP1 and other transcription factors, including NRs, in different contexts. Currently, GRIP1 cistromes are few: genome-wide occupancy of hGRIP1 has only been described in the MCF7 breast cancer line52; in murine cells, GRIP1 cistromes were reported in cardiomyocytes, prostate and liver tissues50,53,54. Its distribution in macrophages under conditions of acute GC stimulation has not been previously evaluated, although certain levels of co-occupancy with GR have been reported in anti-inflammatory (“M2”) BMMΦ generated via long-term GC-driven polarization followed by a 3-h exposure to LPS55. Given a wealth of recent studies on transcriptionally and epigenetically distinct states of macrophage activation56,57,58, future assessment of the role of GRIP1 in macrophage programming represents an extremely fruitful direction to pursue.
Mechanisms underlying specificity in cofactor utilization remain largely unresolved. With over 300 proteins reportedly participating in GR signaling4, it is reasonable to speculate that “more selective” non-GRIP1 components may dictate its recruitment and function. Here we describe GR-driven mobilization of CDK9 and GRIP1 phosphorylation on the 4S cluster (S469, S487, S493, and S499) as a more refined mechanism by which GR directs its own coregulator to activation complexes associated with a subset of canonical and anti-inflammatory genes (Fig. 7). Conceivably, differential GRIP1 phosphorylation imparts a deeper level of specificity to its action. Indeed, our analysis revealed that pS469-GRIP1 occupied 44% of total GRIP1 binding sites and that different isoforms existed in GR:GRIP1 complexes within the same cluster of GBS. A comprehensive mapping of GRIP1 phospho-isoform binding, as ChIP-seq quality antibodies to individual sites become available, would be a promising avenue for future studies. It is critical to acknowledge, however, that this approach is constrained by the properties of phospho-specific antibodies, epitope accessibility and local chromatin features to a much greater extent than transcription factor binding analysis.
Mechanistically, GRIP1 phosphorylation may have multiple non-mutually exclusive outcomes. We showed that loss of phosphorylation attenuated the ability of GRIP1 to localize to a specific GBS. Another possibility is that the 4pS cluster (or less phosphorylated variants thereof) represents a novel protein-binding interface. Phosphorylation is a powerful modulator of protein:protein interactions: phosphorylation of transcriptional cofactors CARM1 and LSD1 was recently shown to even bypass a requirement for ligand in gene activation by Estrogen Receptor-α59. In fact, phosphorylation of GR itself creates a new surface permissive for binding of certain coregulators while blocking others60. Interrogation of this mechanism via proteomic approaches holds the promise of uncovering important modulators of GR:GRIP1 actions in macrophages.
This is the first report describing CDK9 occupancy at an NR response element and its involvement in factor-specific transcriptional regulation. CDK9 is a key component of the Pol II elongation machinery, which makes its functions in more specific transcriptional pathways difficult to assess. Our data argue that detection of CDK9 at the GREs is not a “spill-over” from the TSS due to spatial proximity. Indeed, no CDK9 was detected at the SGK1 GRE at −1 kb despite pronounced GC-induced CDK9 recruitment to the promoter 1 kb away. A scenario wherein, instead, GR recruits CDK9 to modify GRIP1 at a GBS is corroborated by the observation of GR:GRIP1:CDK9 ternary complexes in GC-treated macrophages. We note that this interaction was only detectable after dual crosslinking and could potentially be DNA-dependent. Whether phosphorylation precedes or follows GR:GRIP1 DNA binding is not directly assessable in our experimental system. However, in light of the specificity of pGRIP1 recruitment even in the context of the same gene, our findings are consistent with an established model in which the GRE serves as an allosteric ligand for GR, shaping its structure and, thus, specifying cofactor composition. Given that phosphorylation strictly depends on the GR:GRIP1 interaction, we posit that DNA, even if not required for phosphorylation per se, greatly enhances the stability of the GR:GRIP1 complex and thereby increases substrate availability for CDK9. We also do not exclude the possibility that additional GRIP1 kinases target the 4S cluster in a combinatorial or inter-dependent manner whereby CDK9 phosphorylates a specific serine, which primes phosphorylation of an adjacent serine by another kinase. CDK9 itself is increasingly recognized as a potential drug target in cancers, AIDS, and is being tested in mouse models of arthritis61, highlighting the importance of better understanding its diverse functions.
Intriguingly, GRIP1 phosphorylation is restricted to GR activation complexes with no apparent contribution to GRIP1 corepressor functions in the gene panel tested (Fig. 7). Because GC and TLR signaling are mutually antagonistic, we considered the possibility that LPS-induced pathways globally inhibit GRIP1 phosphorylation, perhaps by imparting modifications to GRIP1 precluding phosphorylation or upregulating a putative GRIP1 phosphatase. Unexpectedly, and despite a decrease of whole-cell GRIP1 phosphorylation, the occupancy of pGRIP1 and CDK9 specifically at the GBS associated with dexamethasone-activated genes and their induction were fully resistant to LPS. How this selectivity is accomplished remains to be explored, however, given relatively low levels of GRIP1 in macrophages, signal-induced phosphorylation could serve as a mechanism that enables GRIP1 to engage in mutually complementary anti-inflammatory actions at both GR-activated and GR-repressed genes at the expense of genes whose glucocorticoid regulation is not essential in inflammatory contexts.
NR coregulators are emerging as potential therapeutic targets due to the striking phenotypes of their deletion and documented deregulation in disease (for review, see ref. 62). Targeting NR coregulators in future therapeutics will likely add to the arsenal of molecules that affect NR signaling pathways, which comprise over 20% of current pharmaceuticals, with GCs being the most commonly prescribed class of drugs worldwide63. A non-redundant, phosphorylation-specified function of GRIP1 as GR coactivator complements its role as a GR corepressor7,20,22 in the context of macrophages and inflammation and may represent an important avenue toward achieving drug selectivity.
C57BL/6 mice (National Cancer Institute, Charles River Laboratories; strain code 556) and their transgenic derivatives were maintained in the Hospital for Special Surgery and Weill Cornell Barrier Animal Facility in full compliance with the protocol approved by the Institutional Animal Care and Use Committee. Homozygous WT (wt/wtGRIP1 fl/fl) and GRIP1 KO (LysM-CreGRIP1 fl/fl) mice were generated previously31.
GRIP1 KO and WT mice were injected intraperitoneally with 5 mg kg−1 of LPS (Sigma) and monitored for 36 h. Mice were weighed at the time of injection and 24 h later.
For sorting of peritoneal macrophages, animals were euthanized via CO2 inhalation after 12 h of 5 mg kg−1 LPS i.p. administration and peritoneal gavages with PBS performed. Antibody staining for flow cytometry included: CD45-PerCP-C5.5 (anti-mouse CD45, clone 30-F11), Cd11b-PE (anti-mouse/human CD11b, clone M1/70), CD3-FITC (anti-mouse CD3e, clone 145-2C11), CD11c-FITC (anti-mouse CD11c, clone N418), Gr1-FITC (anti-mouse Ly-6G/Ly-6C (Gr1), clone RB6-8C5), B220-FITC (anti-mouse/human CD45R/B220) (Biolegend; 1:100 dilution each).
Serum GC levels were determined using the Corticosterone ELISA kit (Abcam, ab108821) and as per manufacturer’s directions. Serum was collected from the blood of euthanized mice12 h after 5 mg kg−1 LPS i.p. injection.
Cell culture and treatments
THP1 cells (ATCC TIB-202) were maintained in RPMI-1640 (Invitrogen) supplemented with 10% fetal bovine serum (FBS; Atlanta Biologicals) and 5–10 nM β-mercaptoethanol (Sigma). THP1 cells were differentiated by 25 ng ml−1 phorbol myristate acetate (Sigma) for 18–24 h followed by a 48 h to obtain THP1 MΦ. Small hairpin (sh)GRIP1 and scrambled shSCR cell lines were generated via lentiviral knockdown as described below. mGRIP1 WT and S469A/S487A/S493A/S499A (4A) were generated via lentiviral overexpression in the shGRIP1 parental line as described below.
Peripheral blood mononuclear cells were obtained from leukocyte preparations of healthy volunteers (New York Blood Center) and separated by Ficoll (Invitrogen) density gradient centrifugation. CD14+ human monocytes were purified from PBMC using magnetic anti-CD14 beads (Miltenyi). Positively selected monocytes were cultured in RPMI-1640 with 10% FBS, l-glutamine (Invitrogen), penicillin/streptomycin (P/S; Invitrogen) and 20 ng ml−1 recombinant human macrophage colony stimulating factor (Peprotech) for 72 h to obtain monocyte-derived hMΦ.
BMMΦ were prepared from 8- to 10-week-old male mice as described22. In brief, tibia and femur bone marrow was flushed and incubated in 1 g l−1 glucose-containing DMEM (Invitrogen) supplemented with 20% FBS and 20% L-Cell conditioned media for 5 days. Adherent cells were then scraped and plated at 2 × 107 in 150 mm plates in DMEM—20% FBS to be treated the following day.
IBMMΦ were generated previously via stable introduction of Raf and Myc64 and maintained in DMEM containing 1 g l−1 glucose supplemented with 10% FBS and P/S. Single guide (sg)CDK9 and scrambled sgSCR cell lines were generated via lentiviral knockdown as described below.
For cell treatments, 100 nM dexamethasone (Sigma) and 10 ng ml−1 LPS (Sigma) were used. For kinase inhibitor experiments, the indicated doses of flavopiridol (FVP) (to 50–100 nM final) were added to cell culture media 30 min before subsequent treatments. For global transcription blockade, triptolide (Abcam) was added to a final concentration of 10 μM 15 min prior to subsequent treatments.
Lentiviral knockdown and overexpression
HEK 293T cells (ATCC) were prepared at 75–90% confluency in Opti-MEM (Invitrogen) supplemented with GlutaMAX (Invitrogen), Sodium Pyruvate (Invitrogen) and 5% FBS and transfected using Lipofectamine 3000 and P3000 reagent (Invitrogen) with the packaging plasmids psPAX2 (Addgene) and pMD2.G (Addgene) and one of the following plasmids: shGRIP1 plasmid, shSCR control, WT mGRIP1, 4A mGRIP1, sgCDK9, or sgSCR control. Six hours post transfection, media was removed and replaced with fresh media containing P/S. Viral media was collected 30 h and 52 h post transfection. Lentivirus was concentrated using Centricon-70 Plus Centrifugal filters (Millipore) and added to THP1 or IBMMΦ cells at an MOI of 50:1 in the presence of 5 μg ml−1 polybrene (Sigma). Cells were positively selected by antibiotic resistance [200 ng ml−1 puromycin (Sigma) or 300 μg ml−1 geneticin/G418 (Invitrogen) for 1–2 week] or by cell sorting at the Weill Cornell Flow Cytometry Core on a FACS Aria II using fluorometric markers—mCherry, mAmetrine or TagBFP.
Immunoblotting and protein immunoprecipitations
Whole cell extracts were prepared using standard procedure in RIPA buffer (10 mM Tris-HCl pH 8.0, 1 mM EDTA, 0.5 mM EGTA, 140 mM NaCl, 5% glycerol, 0.1% Na deoxycholate, 0.1% SDS, 1% Triton X-100). Nuclear extracts were prepared using NE-PER Nuclear and Cytoplasmic Extraction Reagents (Thermo) following manufacturer’s instructions. The following inhibitors were used: Protease Inhibitor Cocktail powder (Sigma, P2714), Phosphatase Inhibitor Cocktail 3 (Sigma, P0044), 1 mM phenylmethylsulfonylfluoride, 1 mM sodium orthovanadate, and 1 mM sodium fluoride. Commercial antibodies were used against GRIP1 (Abcam, ab10491, 1:2000 and BD, 611319, 1:500), GR (Santa Cruz, sc-1004x, 1:1000), CDK9 (Santa Cruz, sc-8338x, 1:1000), HSP90 (Cell Signaling, 4874 S, 1:2000) and GST (Abcam, ab1956, 1:500). Immunoblotting with phosphosite-specific antisera was performed at 1:3000, except for anti-pS469 that was used at 1:500. Precision Plus Protein Dual Color Standards (Biorad) were used to identify molecular weights. Blots shown are representative of ≥3 independent experiments. Densitometric analysis of immunoblots was performed using ImageJ (NIH).
For IPs, cells were double cross-linked with 2 mM disuccinimidyl glutarate (DSG, Proteochem) for 30 min at RT followed by 1% methanol-free formaldehyde (Thermo) for 10 min at RT. The reaction was quenched by 0.125 M glycine for 5 min. Cells were then washed with PBS, scraped and lysed in RIPA buffer + inhibitors. GR IPs were performed using mouse anti-GR (Santa Cruz, G-5, sc-393232) at 1:100 with 40 μl of pre-washed Dynabeads Protein A (Novex, Thermo) O/N at 4 °C and were washed 5× in RIPA buffer. IP samples and inputs were de-crosslinked at 95 °C for 5–10 min. Immunoblotting was performed using rabbit polyclonal antibodies as described above.
In vitro kinase assays
Recombinant WT and 4A GST–GRIP1322–631 fragments were produced in E. coli and purified as described23 and cyclin T1-CDK9 was produced in baculovirus. Assays were performed in Tris-Cl (pH 7.6), 5 mM DTT, 5 mM MgCl2 with 10 μCi of [γ32P]-ATP (6000 Ci mM −1) or 40 μM ATP. Visualization was performed by immunoblotting as described above or by autoradiography and Coomassie blue staining.
RNA isolation and RT-qPCR
Total RNA was isolated from cells with the RNeasy Plus Mini Kit (Qiagen), subjected to random-primed cDNA synthesis, and gene expression analyzed by qPCR with Maxima Sybr Green/ROX/2x master mix (Fermentas) on StepOne Plus real-time PCR system (Applied Biosystems) using standard protocols and the δδCt method. Primers are listed in Supplementary Table 1.
ChIP and ChIP-seq
THP1 MΦ, hMϕ, and BMMΦ were double-crosslinked and prepared for sonication as described previously31. Cross-linked chromatin was sonicated using a Bioruptor Pico (Diagenode) for THP1 MΦ and hMΦ or an S220 Ultrasonicator (Covaris) for BMMΦ to generate DNA fragments ∼150–600 bp. Inputs were taken from cleared lysates and the rest were incubated for 4 h at 4 °C with the following antibodies to precipitate protein:DNA complexes: GR (Santa Cruz, M20x, sc-1004x or N499), GRIP1 (Abcam, ab10491 or Bethyl A300-346A), phospho-specific GRIP1 antibodies, or CDK9 (Santa Cruz, H169x, sc-8338x). An aliquot of 40–50 μl of pre-washed Dynabeads Protein A were added per IP and incubated O/N at 4 °C. Beads were washed 8 times in modified RIPA buffer (50 mM HEPES [pH 7.6], 100 mM LiCl, 1 mM EDTA, 1% NP-40, 0.7% Na-deoxycholate) once with TE with sodium chloride (10 mM Tris pH 8.0 and 1 mM EDTA, 50 mM NaCl). Each reaction was then incubated in TE-0.5% SDS-200 μg ml−1 proteinase K for 2 h at 55 °C, followed by 6 h at 65 °C to reverse cross-links. DNA was purified with Qiagen’s PCR purification kit following manufacturer’s directions. Real-time qPCR primers are listed in Supplementary Table 1. For GR, GRIP1 and pGRIP1 ChIP-seq, 10–30 ng of IP or input material was used. The amount and sonication quality of DNA was tested with Qubit (Thermo) and Bionalyzer 2100 (Agilent Technologies) before library construction using Illumina TruSeq ChIP-Seq Library Prep Kit and sequencing by a HiSeq 2500 system (four to six samples/SR lane, 50 bp reads). Library preparation and sequencing was performed by the Weill Cornell Epigenomics Core.
Human-specific shRNAs to GRIP1 were cloned into pMK1221 (Addgene #84220), an RNA Pol II-driven lentivirus shRNA vector. The ability of individual shRNAs to knock-down GRIP1 in NALM-6 cells (ATCC CRL-3273) after lentiviral transduction was assessed by western blot65. The following shRNA KD GRIP1 worked most efficiently and was used: GRIP1 Sense Strand Sequence: TAGACCTAATTTGTAGACTTAA
Mouse WT and 4A full-length GRIP1 constructs were created from mouse cDNA stepwise using the QuikChange II Site Directed Mutagenesis Kit (Agilent). Full-length murine WT and 4A were BFP-tagged at the N-Terminus through cloning into the pTag-BFP-C vector (Evrogen) and PCR-cloned using Q5 High-Fidelity DNA Polymerase (NEB) and T4 DNA ligase (NEB) in-frame into the pWPI vector (Addgene) using the following primers:
CDS Start + PmeI: 5′-TAAGCAGTTTAAACATGAGCGAGCTGATTAAGGAG-3′
CDS End + PmeI: 5′-TGCTTAGTTTAAACTCAGCAGTATTTCCGAGATGC- 3′
sgRNA that targeted CDK9 or no specific target (sgSCR) were cloned into the all-in-one lentiCRISPR v2 vector (Addgene), in which the selection marker puromycin was replaced by the fluorescent protein mAmetrine.
All constructs were confirmed by sequencing.
Sample sets were compared by unpaired, two-tailed Student’s t-test with P < 0.05 set as a significance threshold when only two samples were being compared except in Supplementary Fig. 9c where P < 0.1 was set as a threshold.
One-way ANOVA with Dunnett’s multiple comparison test was used when two or more samples were being compared to a control sample. One-Way ANOVA with Bonferroni’s multiple comparison test was used when three or more samples were being compared with two or more crosswise comparisons. P < 0.05 was set as a significance threshold.
Mann–Whitney test was used when data distribution deviated from normal. P < 0.05 set as a significance threshold.
Survival analysis was performed using Kaplan–Meier analysis and the log-rank test with P < 0.05 as a significance cutoff.
ChIP-seq statistical analysis
Sequencing quality control was performed using FASTQC and adapters, when needed, were trimmed using trimmomatic. 50 bp single-end reads were aligned to the human genome (GRCh37/hg19) or mouse genome (mm10) with bowtie2. Aligned BAM files were converted into bigwig format for data visualization purposes. GR peaks in BMMΦ were called using the Hotelling Observer signal filtering algorithm implemented in CLC BIO genomics workbench with P < 0.01 as a significance threshold66. Peak calling for all other data sets was performed with MACS2 with the following parameters:
for GR in THP1 MΦ: --format = BAM --gsize 2451960000 --bw = 300 ---slocal 1000 --llocal 10000 --keep-dup 1 -qvalue 0.01;
for GRIP1 in BMMΦ: --format = BAM --gsize 2150570000 --bw = 200 --to-large --ratio 1.0 --slocal 1000 --llocal 10000 --keep-dup 1 –pvalue 0.0001;
for GRIP1 in THP1 MΦ --format = BAM --gsize 2451960000 --bw = 200 --ratio 1.0 --slocal 3000 --llocal 15000 --keep-dup 1 --pvalue 1e-05
with a matching input file to estimate background read distribution. pS469 peaks in dexamethasone-treated samples were called vs. pS469 untreated samples to only obtain dexamethasone-induced peaks with the following parameters: --format = BAM --gsize 2451960000 --bw = 200 --to-large --ratio 1.0 --slocal 1000 --llocal 100000 --keep-dup 1 --pvalue 0.0001.
All called peaks were filtered against ENCODE blacklisted human and mouse regions with empirically high mappability67.
Consensus GR peaks were determined using subsetByOverlaps function from R GenomicRanges package and were used for further set analyses with the minimum overlap of 1 nt and visualized with makeVennDiagram function from ChIPpeakAnno package.
Because GRIP1 peak sets from individual GRIP1 replicas form larger overlaps with GR peak set than between each other, we defined GRIP1 union peaks set as following: (GR GRIP1_rep1 ∩ GR) U (GR GRIP1_rep2 ∩ GR) (Supplementary Figs. 3d and 4d) and used this subset for all further peak set analyses.
Distributions of MACS2 pileup values in different subsets of GR peaks were compared using kernel density estimation from R sm package as previously described31.
Peak annotation relative to known genomics features was performed using ChIPpeakAnno package68 (R, Bioconductor) with TxDb.Mmusculus.UCSC.mm10.knownGene annotation package that is based on the mm10 genome UCSC knownGene table for BMMΦ and TxDb.Hsapiens.UCSC.hg19.knownGene based on the GRCh37/hg19 USCS known Gene table for THP1 MΦ.
The functional annotation of peak-associated genes was performed using the R interface (https://github.com/jokergoo/rGREAT) for GREAT69, the whole genome as a background and the “basal plus extension” gene association rule with the following parameters: adv_upstream = 5.0kb, adv_downstream = 1.0 kb, adv_span = 100 kb, MSigDB (Broad Institute) was used as a source of reference for functional gene sets. The significance of gene set enrichment was evaluated using FDR-adjusted hypergeometric test and the top 15 enriched gene sets were selected.
Ab initio analysis of overrepresented sequences in ChIP-seq peaks was performed using MEME-ChIP suite with MEME, DREME to determine overrepresented sequences and CentriMO to determine sequences with positional bias. E-values estimate the expected number of motifs in an experimental set of sequences compared to random sequences of the similar size. Sequencing motifs with E-values under 0.0001 were considered significant.
All sequencing data have been deposited into GEO database under the accession number GSE99887. All relevant data are available from the authors.
Medzhitov, R. Inflammation 2010: new adventures of an old flame. Cell 140, 771–776 (2010).
Nathan, C. & Ding, A. Nonresolving inflammation. Cell 140, 871–882 (2010).
Webster, J. I., Tonelli, L. & Sternberg, E. M. Neuroendocrine regulation of immunity. Annu. Rev. Immunol. 20, 125–163 (2002).
Weikum, E. R., Knuesel, M. T., Ortlund, E. A. & Yamamoto, K. R. Glucocorticoid receptor control of transcription: precision and plasticity via allostery. Nat. Rev. Mol. Cell Biol. 18, 159–174 (2017).
Vandevyver, S. et al. Glucocorticoid receptor dimerization induces MKP1 to protect against TNF-induced inflammation. J. Clin. Invest. 122, 2130–2140 (2012).
Ronchetti, S., Migliorati, G. & Riccardi, C. GILZ as a mediator of the anti-inflammatory effects of glucocorticoids. Front. Endocrinol. 6, 170 (2015).
Chinenov, Y., Coppo, M., Gupte, R., Sacta, M. A. & Rogatsky, I. Glucocorticoid receptor coordinates transcription factor-dominated regulatory network in macrophages. BMC Genom. 15, 656 (2014).
Clark, A. R. Anti-inflammatory functions of glucocorticoid-induced genes. Mol. Cell. Endocrinol. 275, 79–97 (2007).
Coutinho, A. E. & Chapman, K. E. The anti-inflammatory and immunosuppressive effects of glucocorticoids, recent developments and mechanistic insights. Mol. Cell. Endocrinol. 335, 2–13 (2011).
De Bosscher, K. & Haegeman, G. Minireview: latest perspectives on antiinflammatory actions of glucocorticoids. Mol. Endocrinol. 23, 281–291 (2009).
Vandevyver, S., Dejager, L., Tuckermann, J. & Libert, C. New insights into the anti-inflammatory mechanisms of glucocorticoids: an emerging role for glucocorticoid-receptor-mediated transactivation. Endocrinology 154, 993–1007 (2013).
Rollins, D. A., Coppo, M. & Rogatsky, I. Minireview: nuclear receptor coregulators of the p160 family: insights into inflammation and metabolism. Mol. Endocrinol. 29, 502–517 (2015).
York, B. & O’Malley, B. W. Steroid receptor coactivator (SRC) family: masters of systems biology. J. Biol. Chem. 285, 38743–38750 (2010).
Torchia, J. et al. The transcriptional co-activator p/CIP binds CBP and mediates nuclear-receptor function. Nature 387, 677–684 (1997).
Hong, H., Kohli, K., Trivedi, A., Johnson, D. L. & Stallcup, M. R. GRIP1, a novel mouse protein that serves as a transcriptional coactivator in yeast for the hormone binding domains of steroid receptors. Proc. Natl Acad. Sci. USA 93, 4948–4952 (1996).
Voegel, J. J., Heine, M. J., Zechel, C., Chambon, P. & Gronemeyer, H. TIF2, a 160 kDa transcriptional mediator for the ligand-dependent activation function AF-2 of nuclear receptors. EMBO J. 15, 3667–3675 (1996).
Onate, S. A., Tsai, S. Y., Tsai, M. J. & O’Malley, B. W. Sequence and characterization of a coactivator for the steroid hormone receptor superfamily. Science 270, 1354–1357 (1995).
Heery, D. M., Kalkhoven, E., Hoare, S. & Parker, M. G. A signature motif in transcriptional co-activators mediates binding to nuclear receptors. Nature 387, 733–736 (1997).
Xu, J., Wu, R. C. & O’Malley, B. W. Normal and cancer-related functions of the p160 steroid receptor co-activator (SRC) family. Nat. Rev. Cancer 9, 615–630 (2009).
Rogatsky, I., Luecke, H. F., Leitman, D. C. & Yamamoto, K. R. Alternate surfaces of transcriptional coregulator GRIP1 function in different glucocorticoid receptor activation and repression contexts. Proc. Natl Acad. Sci. USA 99, 16701–16706 (2002).
Rogatsky, I., Zarember, K. A. & Yamamoto, K. R. Factor recruitment and TIF2/GRIP1 corepressor activity at a collagenase-3 response element that mediates regulation by phorbol esters and hormones. EMBO J. 20, 6071–6083 (2001).
Chinenov, Y. et al. Role of transcriptional coregulator GRIP1 in the anti-inflammatory actions of glucocorticoids. Proc. Natl Acad. Sci. USA 109, 11776–11781 (2012).
Flammer, J. R. et al. The type I interferon signaling pathway is a target for glucocorticoid inhibition. Mol. Cell. Biol. 30, 4564–4574 (2010).
Dobrovolna, J., Chinenov, Y., Kennedy, M. A., Liu, B. & Rogatsky, I. Glucocorticoid-dependent phosphorylation of the transcriptional coregulator GRIP1. Mol. Cell. Biol. 32, 730–739 (2012).
Zhou, H. et al. Inhibition of serum- and glucocorticoid-inducible kinase 1 enhances TLR-mediated inflammation and promotes endotoxin-driven organ failure. FASEB J. 29, 3737–3749 (2015).
Wang, T. et al. PER1 prevents excessive innate immune response during endotoxin-induced liver injury through regulation of macrophage recruitment in mice. Cell Death Dis. 7, e2176 (2016).
Hammer, M. et al. Dual specificity phosphatase 1 (DUSP1) regulates a subset of LPS-induced genes and protects mice from lethal endotoxin shock. J. Exp. Med. 203, 15–20 (2006).
Brown, A. R. et al. Kruppel-like factor 9 (KLF9) prevents colorectal cancer through inhibition of interferon-related signaling. Carcinogenesis 36, 946–955 (2015).
Catrysse, L., Vereecke, L., Beyaert, R. & van Loo, G. A20 in inflammation and autoimmunity. Trends Immunol. 35, 22–31 (2014).
Katakura, T., Miyazaki, M., Kobayashi, M., Herndon, D. N. & Suzuki, F. CCL17 and IL-10 as effectors that enable alternatively activated macrophages to inhibit the generation of classically activated macrophages. J. Immunol. 172, 1407–1413 (2004).
Coppo, M., Chinenov, Y., Sacta, M. A. & Rogatsky, I. The transcriptional coregulator GRIP1 controls macrophage polarization and metabolic homeostasis. Nat. Commun. 7, 12254 (2016).
Pan, Y. et al. Metallothionein 2A inhibits NF-kappaB pathway activation and predicts clinical outcome segregated with TNM stage in gastric cancer patients following radical resection. J. Transl. Med. 11, 173 (2013).
Rao, N. A. et al. Coactivation of GR and NFKB alters the repertoire of their binding sites and target genes. Genome Res. 21, 1404–1416 (2011).
Bailey, T. et al. Practical guidelines for the comprehensive analysis of ChIP-seq data. PLoS Comput. Biol. 9, e1003326 (2013).
Chanput, W., Mes, J. J. & Wichers, H. J. THP-1 cell line: an in vitro cell model for immune modulation approach. Int. Immunopharmacol. 23, 37–45 (2014).
Rogatsky, I., Trowbridge, J. M. & Garabedian, M. J. Glucocorticoid receptor-mediated cell cycle arrest is achieved through distinct cell-specific transcriptional regulatory mechanisms. Mol. Cell. Biol. 17, 3181–3193 (1997).
Peterlin, B. M. & Price, D. H. Controlling the elongation phase of transcription with P-TEFb. Mol. Cell 23, 297–305 (2006).
Price, D. H. P-TEFb, a cyclin-dependent kinase controlling elongation by RNA polymerase II. Mol. Cell. Biol. 20, 2629–2634 (2000).
Titov, D. V. et al. XPB, a subunit of TFIIH, is a target of the natural product triptolide. Nat. Chem. Biol. 7, 182–188 (2011).
Baumann, C. T. et al. The glucocorticoid receptor interacting protein 1 (GRIP1) localizes in discrete nuclear foci that associate with ND10 bodies and are enriched in components of the 26S proteasome. Mol. Endocrinol. 15, 485–500 (2001).
Hoang, T. et al. cAMP-dependent protein kinase regulates ubiquitin-proteasome-mediated degradation and subcellular localization of the nuclear receptor coactivator GRIP1. J. Biol. Chem. 279, 49120–49130 (2004).
Puustinen, R., Sarvilinna, N., Manninen, T., Tuohimaa, P. & Ylikomi, T. Localization of glucocorticoid receptor interacting protein 1 in murine tissues using two novel polyclonal antibodies. Eur. J. Endocrinol. 145, 323–333 (2001).
Lazaro, J. B., Bailey, P. J. & Lassar, A. B. Cyclin D-cdk4 activity modulates the subnuclear localization and interaction of MEF2 with SRC-family coactivators during skeletal muscle differentiation. Genes Dev. 16, 1792–1805 (2002).
Frigo, D. E. et al. Mechanism of AP-1-mediated gene expression by select organochlorines through the p38 MAPK pathway. Carcinogenesis 25, 249–261 (2004).
Scott, M. L., Fujita, T., Liou, H. C., Nolan, G. P. & Baltimore, D. The p65 subunit of NF-kappa B regulates I kappa B by two distinct mechanisms. Genes Dev. 7, 1266–1276 (1993).
Paakinaho, V. et al. Single-molecule analysis of steroid receptor and cofactor action in living cells. Nat. Commun. 8, 15896 (2017).
Bhattacharyya, S., Brown, D. E., Brewer, J. A., Vogt, S. K. & Muglia, L. J. Macrophage glucocorticoid receptors regulate Toll-like receptor 4-mediated inflammatory responses by selective inhibition of p38 MAP kinase. Blood 109, 4313–4319 (2007).
Hubner, S., Dejager, L., Libert, C. & Tuckermann, J. P. The glucocorticoid receptor in inflammatory processes: transrepression is not enough. Biol. Chem. 396, 1223–1231 (2015).
Patchev, A. V. et al. Insidious adrenocortical insufficiency underlies neuroendocrine dysregulation in TIF-2 deficient mice. FASEB J. 21, 231–238 (2007).
Stashi, E. et al. SRC-2 is an essential coactivator for orchestrating metabolism and circadian rhythm. Cell Rep. 6, 633–645 (2014).
Dasgupta, S. et al. Coactivator SRC-2-dependent metabolic reprogramming mediates prostate cancer survival and metastasis. J. Clin. Invest. 125, 1174–1188 (2015).
Zwart, W. et al. Oestrogen receptor-co-factor-chromatin specificity in the transcriptional regulation of breast cancer. EMBO J. 30, 4764–4776 (2011).
Reineke, E. L. et al. Steroid receptor coactivator-2 is a dual regulator of cardiac transcription factor function. J. Biol. Chem. 289, 17721–17731 (2014).
Qin, J. et al. Androgen deprivation-induced NCoA2 promotes metastatic and castration-resistant prostate cancer. J. Clin. Invest. 124, 5013–5026 (2014).
Uhlenhaut, N. H. et al. Insights into negative regulation by the glucocorticoid receptor from genome-wide profiling of inflammatory cistromes. Mol. Cell 49, 158–171 (2013).
Xue, J. et al. Transcriptome-based network analysis reveals a spectrum model of human macrophage activation. Immunity 40, 274–288 (2014).
Ehrchen, J. et al. Glucocorticoids induce differentiation of a specifically activated, anti-inflammatory subtype of human monocytes. Blood 109, 1265–1274 (2007).
Martinez, F. O. & Gordon, S. The M1 and M2 paradigm of macrophage activation: time for reassessment. F1000Prime Rep. 6, 13 (2014).
Bennesch, M. A., Segala, G., Wider, D. & Picard, D. LSD1 engages a corepressor complex for the activation of the estrogen receptor alpha by estrogen and cAMP. Nucleic Acids Res. 44, 8655–8670 (2016).
Hittelman, A. B., Burakov, D., Iniguez-Lluhi, J. A., Freedman, L. P. & Garabedian, M. J. Differential regulation of glucocorticoid receptor transcriptional activation via AF-1-associated proteins. EMBO J. 18, 5380–5388 (1999).
Krystof, V., Baumli, S. & Furst, R. Perspective of cyclin-dependent kinase 9 (CDK9) as a drug target. Curr. Pharm. Des. 18, 2883–2890 (2012).
Lonard, D. M. & O’Malley, B. W. Nuclear receptor coregulators: modulators of pathology and therapeutic targets. Nat. Rev. Endocrinol. 8, 598–604 (2012).
Ottow, E. & Weinmann, H. Nuclear Receptors as Drug Targets: A Historical Perspective of Modern Drug Discovery (Wiley-VCH Verlag GmbH & Co. KgaA, 2008).
Blasi, E. et al. Selective immortalization of murine macrophages from fresh bone marrow by a raf/myc recombinant murine retrovirus. Nature 318, 667–670 (1985).
Kruth, K. et al. Suppression of B-cell development genes is key to glucocorticoid efficacy in treatment of acute lymphoblastic leukemia. Blood 129, 3000–3008 (2017).
Kumar, V. et al. Uniform, optimal signal processing of mapped deep-sequencing data. Nat. Biotechnol. 31, 615–622 (2013).
ENCODE Project Consortium. An integrated encyclopedia of DNA elements in the human genome. Nature 489, 57–74 (2012).
Zhu, L. J. et al. ChIPpeakAnno: a bioconductor package to annotate ChIP-seq and ChIP-chip data. BMC Bioinform. 11, 237 (2010).
McLean, C. Y. et al. GREAT improves functional interpretation of cis-regulatory regions. Nat. Biotechnol. 28, 495–501 (2010).
We thank the staff of Weill Cornell Epigenomics Core for sequencing help. We are grateful to the Weill Cornell Flow Cytometry Core and STARR Ansary Stem Cell Core for help with flow selection. D.A.R. is supported by the NIH NIAMS T32 AR007281. M.A.S. is supported by the NIH Diversity Supplement 3R01DK099087-01A1S1 and the MSTP grant T32GM007739 from the NIH NIGMS to the Weill Cornell/ Rockefeller/ Sloan-Kettering Tri-Institutional MD-PhD Program. This work is supported by the grants to I.R. from the NIH R01DK099087, the Rheumatology Research Foundation, the DOD CDMRP PR130049 Research Award and The Hospital for Special Surgery David Rosensweig Genomics Center. X.H. is supported by the Ministry of Science and Technology of China National Key Research Project 2015CB943201, National Natural Science Foundation grants 81422019, 81571580, 91642115, 8151101184 and funds from Tsinghua-Peking Center for Life Sciences. M.A.P. is funded by K99/R00 CA149088, the V Foundation and the Roy J. Carver Charitable Trust 01-224. R.P.F. is supported by the NIH grant R01GM104291.
The authors declare no competing financial interests.
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Rollins, D.A., Kharlyngdoh, J.B., Coppo, M. et al. Glucocorticoid-induced phosphorylation by CDK9 modulates the coactivator functions of transcriptional cofactor GRIP1 in macrophages. Nat Commun 8, 1739 (2017). https://doi.org/10.1038/s41467-017-01569-2
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